NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs European Cells and Materials Vol. 29 2015 (pages 314-329) DOI: 10.22203/eCM.v029a24 ISSN 1473-2262
Abstract
It has been reported that surface microstructural dimensions
can inluence the osteoinductivity of calcium phosphates (CaPs), and osteoclasts may play a role in this process. We hypothesised that surface structural dimensions of ≤ 1 μm trigger osteoinduction and osteoclast formation irrespective
of macrostructure (e.g., concavities, interconnected
macropores, interparticle space) or surface chemistry. To
test this, planar discs made of biphasic calcium phosphate (BCP: 80 % hydroxyapatite, 20 % tricalcium phosphate) were prepared with different surface structural dimensions – either ~ 1 μm (BCP1150) or ~ 2-4 μm (BCP1300)
– and no macropores or concavities. A third material was made by sputter coating BCP1150 with titanium (BCP1150Ti), thereby changing its surface chemistry but preserving its surface structure and chemical reactivity. After intramuscular implantation in 5 dogs for 12 weeks,
BCP1150 formed ectopic bone in 4 out of 5 samples,
BCP1150Ti formed ectopic bone in 3 out of 5 samples, and BCP1300 formed no ectopic bone in any of the 5 samples.
In vivo, large multinucleated osteoclast-like cells densely
colonised BCP1150, smaller osteoclast-like cells formed on BCP1150Ti, and osteoclast-like cells scarcely formed
on BCP1300. In vitro, RAW264.7 cells cultured on the
surface of BCP1150 and BCP1150Ti in the presence of osteoclast differentiation factor RANKL (receptor activator
for NF-κB ligand) proliferated then differentiated into
multinucleated osteoclast-like cells with positive tartrate resistant acid phosphatase (TRAP) activity. However, cell proliferation, fusion, and TRAP activity were all signiicantly inhibited on BCP1300. These results indicate that of the material parameters tested – namely, surface microstructure, macrostructure, and surface chemistry
– microstructural dimensions are critical in promoting osteoclastogenesis and triggering ectopic bone formation.
Keywords: Biphasic calcium phosphate, topography, microstructure, osteoclast, osteoinduction.
*Address for correspondence: Noel L. Davison
Xpand Biotechnology
Professor Bronkhorstlaan 10 Bldg 48 3723 MB Bilthoven
The Netherlands
Telephone Number: +31 30 229 7280 FAX Number: +31 30 229 7299 E-mail: noel.davison@gmail.com
Introduction
Certain calcium phosphates (CaPs) can induce de novo
bone formation without exogenous stem cells or growth factors, making them particularly attractive for use as
bone graft substitutes (Ripamonti, 1991; Yuan et al.,
2010). Although the material parameters and biological signalling necessary to induce de novo bone formation
are unclear, osteoinductive CaPs developed by different groups seem to share similar surface structure, speciically
surface topographical features on a (sub)micron-scale. For
instance, hydroxyapatite (HA) with surface micrograins
and micropores induced ectopic bone formation in dogs
and goats, but HA with a denser surface of large, fused grains and few micropores did not (Habibovic et al.,
2005b; Yamasaki and Sakai, 1992; Yuan et al., 1998; Yuan et al., 1999). Similarly, microstructured biphasic
calcium phosphate (BCP) – a mixture of HA and tricalcium phosphate (TCP) – induced de novo bone formation in
the muscle of sheep (Le Nihouannen et al., 2005), goats
(Habibovic et al., 2005b; Yuan et al., 2002), and dogs (Yuan et al., 2010); however, BCP with larger grains and fewer micropores induced less bone formation (Yuan et al.,
2010) or in other cases none at all (Habibovic et al., 2006b).
More recently, the dimensions of surface microstructure have also been shown to be important for osteoinduction – for instance, TCP with submicron-scale surface structure consistently stimulated de novo bone formation in dog
muscle, while TCP with micron-scale surface structure was not at all osteoinductive (Davison et al., 2014b; Zhang et al., 2014). Surface microstructure may also be critical
in triggering osteoinduction by other biomaterials such as titanium (Fujibayashi et al., 2004; Fukuda et al., 2011).
Macroscale features of osteoinductive biomaterials
such as interconnected macropores, particle size, and
surface concavities have also been previously speculated to
be “essential” and “requisite” for de novo bone formation
(Habibovic et al., 2005a; Habibovic et al., 2005b; Magan and Ripamonti, 1996; Yuan et al., 2002). However,
extensive de novo bone can also form in the intramuscular space between non-macroporous, microporous CaP
particles (Yuan and de Bruijn, 2011). Thus, it is still unclear if interparticle space along with microstructure is necessary
for osteoinduction or if de novo bone can also form on a
macroscopically lat surface.
The physicochemical properties of CaPs are also
theorised to be crucial for osteoinduction through the
formation of a crystalline carbonate apatite surface layer after implantation (Daculsi et al., 1989; LeGeros, 2008).
INFLUENCE OF SURFACE MICROSTRUCTURE AND CHEMISTRY ON
OSTEOINDUCTION AND OSTEOCLASTOGENESIS BY BIPHASIC
CALCIUM PHOSPHATE DISCS
N.L. Davison1,2,*, J. Su2, H. Yuan1,2,3, J.J.J.P. van den Beucken4, J.D. de Bruijn1,2,5 and F. Barrère-de Groot2
1MIRA Institute for Biomedical Technology and Technical Medicine, University of Twente, Enschede,
The Netherlands
2Xpand Biotechnology BV, Bilthoven, The Netherlands
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
The solubility of a given CaP (e.g., the HA/TCP ratio in the case of BCP), as well as its microstructure (e.g.,
surface micropore and crystal grain size) contribute to this mineralised surface layer by modulating the dissolution/ reprecipitation of calcium and phosphate ions in body luid (Daculsi et al., 1990). The biological relevance of
surface reactivity and a precipitated layer of carbonate apatite is speculated to be either a direct physicochemical
trigger for osteogenesis (i.e., the differentiation of bone forming osteoblasts from uncommitted precursors) through
elevated local calcium and phosphate levels (Barradas et al., 2013; Beck et al., 2000; Syed-Picard et al., 2013), or a biomimetic template for bone deposition following
osteoblast differentiation by another means (LeGeros, 2008). However, surface reactivity and carbonate apatite precipitation may only be a permissive factor in osteoinduction, not an osteogenic trigger. Taking the case of osteoinductive titanium as an example, Fujibayashi et al.
(2004) reported that although both titanium mesh cylinders and porous blocks formed an apatite layer in simulated body luid in vitro after thermochemical treatment, only the
porous blocks induced ectopic bone formation – potentially due to more complex surface topography (Fujibayashi
et al., 2004). Because surface reactivity and physical
topography can both inluence osteoblast differentiation but are linked to surface architecture, it is currently unknown which, if either, material property plays a prevailing role
in osteoinduction (Curran et al., 2006; Habibovic et al.,
2006a; Vlacic-Zischke et al., 2011; Zhao et al., 2007).
Alternatively, osteoinduction may depend on (pre-) osteoclast activity for osteogenic signals rather than intrinsic physicochemical signals originating from the
material itself (Baslé et al., 1993; Gauthier et al., 2005; Malard et al., 1999). In support of this theory, it has been reported that osteoclastogenesis precedes osteoinduction
by microstructured TCP by several weeks (Akiyama et al., 2011; Kondo et al., 2006), and osteoclast depletion limits (Ripamonti et al., 2010) or completely blocks de novo bone formation by osteoinductive CaPs (Davison et al., 2014a). Recently, we reported a clear link between
TCP microstructure, osteoclastogenesis, and subsequent
de novo bone formation (Davison et al., 2014a; Davison et al., 2014b). However, (pre-)osteoclast differentiation
and activity is inluenced by multiple substrate parameters including surface nano-/microroughness (Makihira et al.,
2007; Webster et al., 2001), solubility (Benahmed et al., 1996; Yamada et al., 1997), and the accompanied release
of nano-/microparticulate (Fellah et al., 2007; Velard et al., 2013), so it is currently unknown if this link also holds
true for less resorbable materials like BCP or titanium. Given the present knowledge, we hypothesised
that surface structure is the preeminent material factor
responsible for the formation of both osteoclast-like
cells and de novo bone. To evaluate this, two BCPs with different surface structure were prepared in the form of planar, non-macroporous discs, thus eliminating the
effects of interconnected macropores, concavities, or interparticle space. To evaluate whether the surface chemistry contributes to osteoinductivity, BCP was also surface coated with titanium. Disc constructs were
implanted in the dorsal muscle of dogs, the classical model
for evaluating osteoinduction, and the formation of de novo bone and multinucleated osteoclast-like cells was
analysed by histology. The effects of surface structure and chemistry on osteoclastogenesis were further evaluated
in vitro using the RAW264.7 pre-osteoclast cell line, as
previously described (Davison et al., 2014b). Osteoclast
differentiation, survival and morphology were measured and quantitatively compared using several biochemical,
histological and morphological techniques.
Materials and Methods Preparation and characterisation of BCP
BCP powder composed of 80 % HA/20 % β-TCP was
prepared by wet precipitation as described elsewhere (Yuan
et al., 2002). The powder was foamed with diluted H2O2 (0.1 %) (Merck, Schiphol-Rijk, Netherlands) at 60 °C to
produce microporous green bodies and then dried. The dry green bodies were subsequently sintered at 1150 °C or
1300 °C for 8 h to achieve surface micro-grains and pores (BCP1150) or larger fused grains and few micropores (BCP1300). Ceramic discs (Ø 9 × 1 mm) were machined from the ceramic bodies using a lathe and a diamond saw
microtome (Leica SP1600). Discs were ultrasonically cleaned in successive baths of acetone, ethanol and
deionised water for 15 min, and then dried at 60 °C.
To obtain a different surface chemistry while preserving the surface microstructure, BCP1150 discs were sputter coated with titanium (BCP1150Ti) using a radiofrequency magnetron unit (Edwards ESM 100) as previously described (Wolke et al., 1998). Both sides of the discs were coated for 15 min at 200 W, resulting in a
visually complete layer of titanium roughly 50nm thick. The elemental composition and distribution of the titanium coating was veriied using electron dispersive spectroscopy (EDS), as previously described (Bongio et al., 2013).
Briely, samples were afixed to metal stubs and scanned by a scanning electron microscope (Philips XL30) equipped with an energy dispersive spectrometer (EDAX, Ametek). The distribution of elements of interest (Ca, P and Ti) was analysed and visually displayed. The associated error for all the EDS analyses was calculated to be less than 10 %.
Surface structure of the materials was characterised by scanning electron microscopy (SEM) (JEOL JSM-5600)
after sputter coating with gold for 90 s (JEOL JFC 1300).
Surface grain and pore size were quantiied in scanning electron micrographs (magniication: 5000×, n = 3 random
locations) by measuring the vertical distance across the
features (n > 50) in Image J software (NIH, Bethesda, MD,
USA).
Crystal chemistry of the materials was analysed by X-ray diffraction (Rigaku Minilex II) scanning the range 2θ = 25-45° (step size = 0.01°, rate = 1° min-1) as previously
described (Davison et al., 2014b). The surface reactivity of
the discs was analysed in simulated physiologic solution
(SPS) (50 mM HEPES, 140 mM NaCl, and 0.4 mM NaN3
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
SPS (8 mL) in a tissue culture multiwell plate incubated at 37 °C, 5 % CO2 for 7 d with gentle shaking. The solution was sampled and refreshed with the same amount (100 μL) after 10 min, 1, 2, 4 h, 1, 4 and 7 d. Calcium
and phosphate released into the solution were quantiied using QuantiChrom (BioAssay System, Hayward, CA, USA) and PhoshoWorks (AAT BioQuest, Sunnyvale, CA, USA) colorimetric assay kits, respectively, following the manufacturers’ instructions. Absorbance was detected using a Zenyth 3100 multimode spectrophotometer.
In vivo study of osteoinduction by BCP constructs Implantation of sandwich constructs
BCP constructs were implanted in the dorsal muscle of dogs
to test their capacity to form ectopic bone. BCP constructs were made by gluing (Cyanoacrylate “Superglue”, Pertex, Cornwall, UK) two discs together with two strips of nylon
wire (~ Ø0.7 mm) in between to create a central gap (Fig.
3A). “Sandwich” shaped constructs were sterilised by
gamma irradiation (> 25 kGy) prior to implantation.
All surgery was conducted at the Animal Centre of Sichuan University in conformance with the institutional
animal ethics committee’s guidelines. Sterile BCP
constructs were implanted in the dorsal muscle of healthy
male mongrel dogs (n = 5 dogs, 1-4 years, 10-15kg) for
12 weeks. Animals were irst given general anaesthesia by
abdominal injection of sodium pentobarbital (30 mg kg−1
body weight) and constructs were implanted into paraspinal muscle pockets created by scalpel incision and blunt
dissection. One construct of each material was implanted in each dog resulting in 3 constructs implanted per animal.
Skin incisions were closed layer by layer with non-resorbable sutures for identiication at harvest. Following surgery, the animals were given daily intramuscular
injections of buprenorphine (0.1 mg per animal) for 2 d and penicillin (40 mg kg-1) for 3 d to relieve pain and prevent
infection. Animals were allowed to undertake full activity and received a normal diet immediately after surgery.
Sample harvest and histological processing
At the end of 12 weeks, the animals were euthanised by
abdominal injection of sodium pentobarbital (60 mg kg-1)
and samples were immediately harvested and ixed in cold phosphate-buffered formalin solution, dehydrated in graded ethanol series, and embedded in methyl methacrylate (MMA) (LTI, Bilthoven, Netherlands) at room temperature. Histological sections (~ 30 μm) of the undecalcified
samples were made using a Leica SP1600 microtome and
stained en bloc with 1 % methylene blue and 0.3 % basic
fuchsin solutions for histological analysis.
Stained histological sections were scanned using a
Dimage Scan Elite 5400II slide scanner (Konica Minolta) for gross evaluation. Bone formation was analysed at 20×
magniication using a light microscope (Nikon Eclipse
E200). More than 10 sections per sample spanning more
than half the construct were analysed for de novo bone
formation by 2 investigators (ND and JS), and the number of samples positive for bone formation per the total number of samples implanted (i.e., bone incidence rate) was recorded.
In vitro studies
Culture of RAW264.7 osteoclasts and C2C12 myoblasts on BCP discs
To model osteoclastogenesis in vitro, murine RAW264.7
macrophages (ECACC, Salisbury, UK) were cultured on
the surface of BCP discs for up to 5 d in the presence of
osteoclast differentiation factor RANKL (receptor activator
for NF-κB ligand) as described previously (Collin-Osdoby et al., 2003). RAW264.7 cells were irst expanded in tissue
culture lasks with basic medium composed of alpha MEM (Lonza, Breda, Netherlands), supplemented with
10 % HyClone FetalClone I serum (Thermo Scientiic,
Waltham, MA, USA) and 1% penicillin-streptomycin (Life Technologies, Merelbeke, Belgium). At ~ 75 % conluence,
cells were scraped loose from the tissue culture lasks, resuspended in basic medium supplemented with RANKL
(40 ng mL-1, Peprotech, London, UK), and seeded on BCP discs (2 × 104 cells cm-2). All discs were heat sterilised in a
dry chamber at 200 °C for 2 h prior to cell culture.
RAW264.7 cells were cultured for 5 d with medium
refreshment (basic medium + RANKL) after 1 d. In our
previous experience with this culture model (Davison
et al., 2014b), cells begin to fuse and differentiate into
osteoclasts by day3, continue fusing through day 4-5,
and undergo apoptosis by day6-7 (Collin-Osdoby et al.,
2003; Takahashi et al., 2007). Therefore, biochemical
assays focused on day 3-5 as the relevant period of osteoclastogenesis. Osteoclast culture experiments were repeated to confirm the results of the various assays
described below.
C2C12 myoblasts were cultured on BCP discs to study
the effects material properties on muscle cells. C2C12 cells
were similarly expanded in basic medium, trypsinised at conluence, and cultured on BCP discs (seeding density
= 2 × 104 cells cm-2) for 5 d. All cells were cultured in a
humidiied incubator maintained at 37 °C and 5 % CO2.
Cell viability, proliferation, and DNA content
The AlamarBlue (AB) luorescent assay (Life Technologies) was used to measure cell viability and proliferation (Nakayama et al., 1997) on BCP. AB measures the
reductive activity inside living cells, and is commonly used in the literature as a more sensitive alternative to formazan-based cell viability assays such as MTT and XTT (Ahmed
et al., 1994; Gloeckner et al., 2001). At various culture time points, cells were incubated with culture medium containing 5 % AB reagent for 2 h in culture conditions and then media samples were collected in a 96-well plate
for luorescent detection (excitation = 530 nm, emission = 590 nm) using a Zenyth Multimode plate reader. Cell
proliferation can be measured by assaying cell viability over time (Nakayama et al., 1997). For this assay, the same
procedure was followed except that AB-containing culture medium was removed and refreshed with normal culture medium, and then continuously cultured until the next time point. For viability and proliferation assays, n = 3 culture replicates were measured.
DNA content was measured in the cell lysate using a CyQuant DNA detection kit (Life Technologies). After 3,
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
in CyQuant cell lysis buffer, as recommended by the manufacturer. Cell lysate was thoroughly homogenised
and sampled from n = 3 replicate discs for measurement
using the kit. A Zenyth 3100 Multimode plate reader was used to detect the luorescent signal of the assay.
Tartrate resistant acid phosphatase (TRAP) activity
Tartrate resistant acid phosphatase (TRAP) activity, an enzyme marker of osteoclast differentiation (Halleen et al., 2001), was measured in RAW264.7 cells cultured on discs after 3, 4 and 5 d by both biochemical activity and
cytochemical staining. TRAP activity in the cell lysate from
n = 3 culture replicates was quantiied by conversion of p-nitrophenylphosphate to p-nitrophenol (pNP) in sodium
acetate buffer (pH 5.8) containing potassium sodium tartrate (10 mM), as reported by Ljusberg et al. (1999).
Cell lysate was obtained by irst rinsing disc-adherent cells with PBS and then freeze-thawing in cell lysis buffer
(0.1 M sodium acetate, 0.1 % Triton X-100, pH5.8). All
reagents were purchased from Sigma Aldrich. Optical absorbance of the assay reaction was measured using a Zenyth multimode spectrophotometer. Absorbance was converted to mM pNP using a standard curve of pNP (Sigma Aldrich) and normalised to viable cell signal from AlamarBlue. TRAP was also visualised on n = 2 disc
replicates using a commercial staining kit (Leukocyte Acid Phosphatase Kit, Sigma Aldrich). Prior to staining, cells were briely rinsed in PBS and ixed in acetone methanol
solution as per the manufacturer’s instructions. Images
were captured using a Nikon SMZ800 stereomicroscope equipped with a Nikon camera.
SEM of osteoclast morphology
Osteoclast morphology was analysed by SEM. Cells
cultured on discs (n = 2) were ixed in 2.5% glutaraldehyde,
dehydrated in a graded ethanol series, and inally dried in hexamethyldisilazane (HMDS; Alfa Aesar, Karlsruhe, Germany). Dehydrated cells were then sputter coated
with gold for enhanced imaging resolution. Osteoclast
size was quantiied in scanning electron micrographs
(400× magniication), by calculating the mean surface area of cells at 3 random locations of replicate discs (n = 2) using automated threshold, edge detection, and
particle analysis functions in ImageJ software (NIH), as previously described (Davison et al., 2014b). Only cells > 400 μm2 were included in the analysis to safely exclude mononuclear cells.
Statistical analysis
Statistical comparisons were performed using One-way ANOVA and Tukey’s post hoc tests; p values < 0.05
were considered signiicant. All statistical analyses were conducted in GraphPad Prism 6.0.
Results BCP characterisation
BCP1150 and BCP1300 with different surface
microstructures were prepared by changing the sintering temperatures, as shown by SEM (Fig. 1A). Quantitatively, BCP1150 contained grains and pores sized ≤ 1 μm in diameter but BCP1300 contained larger, fused grains Fig. 1. Surface characterisation of BCP. Scanning electron micrographs show the difference in surface microstructure
between BCP1150 and BCP1300 and the similarity between BCP1150 and BCP1150Ti with titanium coating
(scale = 10 μm) (A). Surface grain and pore size ≤ 1 μm of BCP1150 were unchanged by titanium coating; however,
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
(~ 3 μm) and larger but fewer micropores (~ 2 μm) (Fig. 1B)). Because no macropore porogens were introduced
during synthesis, neither material contained macropores or substantial concavities. Sputter coating BCP1150 with titanium (BCP1150Ti) did not visibly change the surface microstructure by SEM (Fig. 1A) or the size of the surface
grains and pores (Fig. 1B) versus BCP1150.
The crystal chemistry of the materials was conirmed by X-ray diffraction (XRD) to be BCP containing
80-85 % HA and 15-20% TCP (Fig. 2A). Coating BCP1150
with titanium did not substantially alter the XRD spectra. The surface reactivity of the materials was analysed by
measuring calcium and phosphate ion release in simulated
physiologic solution (SPS) at pH7 and pH3 (Fig. 2B). At neutral pH, all three materials released similar amounts of ions over time, but at acidic pH, ion release from BCP1150 and BCP1150Ti was higher than BCP1300, resulting from the increased surface area of the microstructure. There was no change in ion release by BCP1150 with or without the
titanium coating showing that the coating did not change
the chemical reactivity of the material (Fig. 2B).
Sputter coating BCP1150 with titanium resulted in
a visually homogenous layer on all sides of the discs (Fig. 3A). The titanium layer was analysed by EDS, which showed the homogeneously distributed titanium
coating on the surface (Fig. 3B) that remained on the
surface after implantation (Fig. 4). In summary, sputter
coating BCP1150 with titanium resulted in a material
with equivalent microstructure and chemical reactivity but different surface chemistry.
In vivo results
BCP sandwich constructs were implanted into the dorsal
muscle of dogs for 12 weeks to study the effects of surface microstructure and chemistry on osteoinduction. A gap between the BCP discs was created using nylon wire
spacers to allow tissue in-growth and bone formation (Fig.
5A). However, soft tissue formation in the space between the discs and around the nylon wires tended to be weak
for all materials compared to tissue formation on the outer edges of the constructs (Fig. 5B).
The incidence of de novo bone formation was quantiied
by thorough analysis of histological sections. De novo bone
formation was observed in 4 out of 5 BCP1150 constructs, 3 out of 5 BCP1150Ti constructs, and 0 out of 5 BCP1300 constructs (Table 1). For BCP1150 and BCP1150Ti, bone was predominantly formed on the outer surfaces of the constructs (Fig. 6A) rather than on the inner surfaces of the central gap. Although stretches of bone were not thicker
Fig. 2. Chemical characterisation
of BCP. The XRD spectra were equivalent for all three BCP
materials (A). Chemical reactivity
in simulated physiologic solution
(SPS) showed that ion release of
all three materials was equivalent at pH 7, but slightly faster for
BCP1150 with and without titanium coating than BCP1300
at pH 3 (B). Data represents the mean ± S.D. of n = 3 replicate discs, p < 0.0001.
Table 1. Incidence rate of specimens containing de novo bone formation
BCP1150 BCP1150Ti BCP1300
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
Fig. 3. Elemental analysis of BCP1150Ti by electron dispersive spectroscopy (EDS). (A) Overview images of BCP1150
and BCP1150Ti show that discs were appreciably devoid of concavities or macropores and that titanium coating uniformly covered the disc surfaces. (B) Elemental diffraction spectroscopy (EDS) analysis (2,000× magniication)
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
Fig. 4. Elemental analysis of BCP1150Ti explant.After 12 weeks intramuscular implantation, a thin layer of titanium
was still intact on the edge of the BCP115Ti construct cross-section. Scale = 50 μm.
F i g . 5 . I n t r a m u s c u l a r i m p l a n t a t i o n o f B C P sandwich constructs. BCP sandwich constructs were
made by gluing together two
BCP discs with a central gap
in between them using nylon
wire spacers (A). Constructs were implanted in the dorsal
muscle of dogs for 12 weeks
and histological sections
were stained with methylene
blue and basic fuchsin (B).
Overview images of cross-sections taken through the middle of explants show soft tissue (pink, purple, blue)
formation around the BCP
constructs (brown, black) with limited tissue iniltration
in the gap between the discs.
Tissue often delaminated
f r o m t h e s u r f a c e o f
BCP1300 constructs (black arrows), indicating weak
tissue bonding. Note: few
macropores or concavities
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
than ~ 50 μm and generally spanned less than several
hundred μm long, cuboidal osteoblasts were seen forming
new bone and osteocytes were present in bone lacunae (Fig. 6A). Bone area was not quantiied by histomorphometry
due to the small amounts present.
Multinucleated osteoclast-like cells extensively covered the surface of BCP1150, but were smaller and less organised on BCP1150Ti (Fig. 6B). For both materials, osteoclast-like cells adhered to the material adjacent
to de novo formed bone. In contrast to BCP1150, with
and without a titanium coating, BCP1300 was largely encapsulated by fibrous tissue and contained scarce multinucleated osteoclast-like cells (Fig. 6B).
In vitro results
Cell viability and proliferation
To further investigate the effects of BCP surface structure and chemistry on osteoclast-like cell formation, RAW264.7
macrophages were cultured on BCP discs and differentiated
into osteoclast-like cells using RANKL. At day 3, 4 and 5,
Fig. 6. Histology of intramuscularly implanted BCP sandwich constructs. (A) At 10× magniication of the outer
surface of the constructs (top row), a thin layer of ectopic bone (red/pink) was evident on BCP1150 and BCP1150Ti, but only ibrous tissue (blue/purple) was present on BCP1300. Scale = 100 μm. At 40× magniication (bottom row),
osteocytes (white arrowheads) resided in characteristic bone (asterisk) lacunae on the surface of both BCP1150 and BCP1150Ti. Flattened osteoblasts (black arrowheads) surrounded by condensing matrix lanked the ectopic bone
formed on BCP1150. Scale = 25 μm. (B) Multinucleated cells (black arrows) formed on BCP1150 were larger and
more densely organised than on BCP1150Ti, while no discernible multinucleated cells were present on the surface of
BCP1300 (left column). Scale = 25 μm. Multinucleated osteoclast-like cells bordered ectopic bone on BCP1150 and
BCP1150Ti; however, these cells appeared smaller and less fused on BCP1150Ti than on BCP1150 (right column). The intact titanium layer on BCP1150Ti was evident throughout the micrographs (thin black strip on the construct
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
DNA content from cells cultured on BCP1150 was ~ 3-5
times greater than on BCP1300 (day 3: p <0.0001; day 4: p = 0.0001; day 5: p = 0.004) (Fig. 7A). DNA content
from cells cultured on BCP1150Ti was also signiicantly
greater than on BCP1300 (p <0.01), at levels similar to
BCP1150 at day 4 and 5 (Fig. 7A). These data indicated
that the difference in titanium coating had little effect on
cell growth; however, the difference in microstructure had a pronounced effect. After 5 d of culture, cell viability
was ~ 2× higher on both BCP1150 and BCP1150Ti than on BCP1300 (both p < 0.0001) (Fig. 7B). Further, cell
viability was higher for BCP1150Ti than for BCP1150
(p = 0.002) (Fig. 7B).
RAW264.7 cell proliferation was analysed on BCP1150 and BCP1300 by measuring cell viability over time normalised to the viability at the time of seeding (d0) (Fig. 7C). BCP1150Ti was not included in this analysis, focusing only on the effects of surface structure, not surface chemistry. At day1, cell viability was similar
on the materials suggesting that initial cell attachment
was equivalent. By day 3, RAW264.7 cell proliferation was signiicantly greater for BCP1150, resulting in ~ 2×
greater viability than on BCP1300 (p = 0.001). The same
difference in cell viability was maintained through day 4
(p = 0.004) and day 5 (p = 0.005), indicating that BCP1150
stimulated signiicantly more proliferation of RAW264.7 cells than BCP1300 over the entire culture period. In fact, RAW264.7 cells cultured on BCP1300 did not proliferate
between 1 and 5 d in culture (Fig. 7C). To evaluate if interactions with BCP1300 inhibited the proliferation of
other cell types, C2C12 myoblasts were also cultured on
the materials, but in contrast, these cells proliferated in
typical logarithmic fashion on BCP1300 and to a greater extent than on BCP1150 by day 4 and 5 (p = 0.003 and p = 0.001, respectively) (Fig. 7D).
In sum, BCP1150 promoted signiicantly higher cell growth and viability of RAW264.7 (pre-)osteoclasts than BCP1300 in a process that was not adversely affected by
Fig. 7. Cell viability and proliferation on BCP in vitro. RAW264.7 cells were cultured on BCP discs in the presence
of RANKL for 5d to stimulate osteoclast formation. DNA content in the lysate from cells cultured on BCP1150 was signiicantly higher than on BCP1300 at day3, 4 and 5. DNA content was different between BCP1150 and BCP1150Ti at day 3 and 4; however, they were equivalent by day 5 (A). At day5, osteoclast viability was also signiicantly
higher on BCP1150 and BCP1150Ti than on BCP1300, as measured by AlamarBlue (AB) metabolic indicator (AB RFU = AB relative luorescent units) (B). Comparing the effects of only surface microstructure, RAW264.7 cells
were again cultured in the presence of RANKL on BCP1150 and BCP1300 and cell viability was measured over time indicating cell proliferation. After 1 day, viability was equivalent between BCP1150 and BCP1300, but by days 3, 4
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
titanium coating; however, this response was not universal to other cell types such as C2C12 myoblasts.
TRAP activity
TRAP enzyme activity in the RAW264.7 cells was assayed both biochemically in the cell lysate and cytochemically by staining. Biochemical TRAP activity in the lysate of cells cultured on BCP1150 was signiicantly higher than that of BCP1300 at day 3 (~ 4×, p <0.0001), day 4 (~ 3×, p <0.0001) and day 5 (~ 2×, p = 0.008) (Fig. 8A). Cells
cultured on BCP1150Ti also expressed signiicantly more TRAP activity than BCP1300 at day 3 (~ 2×, p = 0.023)
and day 4 (~ 2.5×, p = 0.002), although at day 5 there was no statistical difference (p = 0.194). Cellular TRAP activity
was different between BCP1150 and BCP1150Ti at day 3
(~ 1.8×, p = 0.004); however, by day 4 and 5 there was no statistical difference (p = 0.144 and 0.102, respectively)
(Fig. 8A).
To visually confirm the biochemical results, cells were stained for TRAP at the same time points (Fig. 8B).
Fig. 8. Tartrate resistant acid phosphatase (TRAP) activity of RAW264.7 osteoclasts cultured on BCP. Biochemical
TRAP activity in the cell lysate was signiicantly higher on BCP1150 than BCP1300 throughout the culture period, as well as BCP1150Ti at day 3 (A). By cytochemical staining, osteoclasts formed on BCP1150 are consistently
larger, denser, and more intensely stained than on BCP1300, in agreement with the biochemical assay (overview
scale = 2 mm; detail scale = 500 μm) (B). Visualisation of TRAP staining was not possible on BCP1150Ti discs, due
to their dark colour. Biochemical TRAP activity (mM pNP normalised to viable cells, AB RFU) represents the mean
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
Visualisation of TRAP staining on BCP1150Ti was not possible because of the dark colour of the coating. A clear difference in osteoclast fusion and TRAP activity between BCP1150 and BCP1300 was observed (Fig. 8B): cells were substantially larger and more intensely stained on
BCP1150 at all time points. On BCP1150, numerous
cell-cell junctions were observed between densely distributed
cells; in contrast, on BCP1300, cell junctions were sparse
likely owing to less cells present (Fig. 8B), in conirmation of the cell viability and DNA assays (Fig. 7).
Osteoclast morphology and size
Osteoclast morphology and size were analysed by SEM at day 5, corresponding with the peak of TRAP activity and cell fusion visualised by TRAP staining (Fig. 9). On BCP1150, fused cells were massive (~ 4,000 μm2) and
tightly attached to the BCP surface in an extensive cell network. Single cells were generally found in clusters, with partially fused cell membranes. In contrast, fused cells on BCP1150Ti were ~ 75 % smaller (~ 1,000 μm2, p = 0.002) and appeared rounder and less spread out on the surface. On BCP1300, fused cells were also smaller than on BCP1150 (~ 1,500 μm2, p = 0.008), and often appeared to be apoptotic
or necrotic with deteriorating cell membranes. Fewer cells
were present on BCP1300 than BCP1150 and BCP1150Ti, in agreement with the cell viability and DNA assays.
Discussion
In the present results, BCP and titanium-coated BCP with small surface microstructural dimensions (~ 1 μm)
promoted osteoclast-like cell formation along with de novo bone formation, while larger surface architecture (~ 2-4 μm) inhibited these effects. Moreover, macro-scale
features such as concavities, macropores, or interparticle space were unnecessary to stimulate this response. These
in vivo observations were further investigated in vitro
using a previously described osteoclastogenesis model (Davison et al., 2014b). Notably, osteoclast survival
and differentiation were significantly promoted by the osteoinductive surface structure of BCP1150 and BCP1150Ti versus the non-inductive surface structure of
BCP1300. Pre-osteoclast proliferation was also stunted by
BCP1300 versus BCP1150; however, C2C12 myoblasts
proliferated strongly on BCP1300 versus BCP1150, Fig. 9. Scanning electron microscopy (SEM) of osteoclasts formed on BCP.SEM micrographs captured at day 5 show
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
illustrating that BCP1300 was not universally detrimental to cell proliferation. These in vitro results may also explain
why few multinucleated cells but abundant soft tissue was
present on this surface in vivo. Regarding osteoclast fusion and size, BCP1150 stimulated the formation of large, fused osteoclasts that were ~ 2-4 times larger than those formed
on either BCP1150Ti or BCP1300 in vitro. In this way, surface microstructural dimensions of ~ 1 μm promoted
(pre-)osteoclast proliferation, differentiation, and survival
versus larger surface structure, while titanium surface
chemistry appeared to limit osteoclast fusion.
At the onset of the present study, it was unclear whether planar, macroscopically lat implants could induce bone formation, based on a lack of direct investigation in the
literature (Barradas et al., 2011). Bone formed on the outside surface of the microstructured constructs, not
only between the discs; thus, the crucial role of surface microstructure on osteoinduction was more clearly isolated
and interparticle space was shown to be dispensable. Still,
the amount of ectopic bone formed in the present study was small in comparison to the ectopic bone formed by a
similar microstructured BCP with macroporous structure,
as previously reported (Habibovic et al., 2006b; Yuan et al., 2010). So, macrostructural features may enhance
bone deposition after it has already been triggered by osteoinductive microstructure.
Ectopic bone also formed on the titanium surface
of BCP1150Ti indicating that surface chemistry is a lexible parameter in the osteoinductive performance of microstructured materials. Rather than being fully sealed,
the line-of-sight sputter deposition of titanium on BCP1150
preserved the chemical reactivity of the BCP substrate and was still intact after implantation. Whereas BCP1150Ti
possessed small surface microarchitecture and similar
dissolution proile of the underlying BCP1150 substrate, other osteoinductive titanium materials described in the literature possess nano-/microarchitecture (Fujibayashi
et al., 2004; Fukuda et al., 2011), and being fully made up of titanium are incapable of releasing calcium or
phosphate ions into solution. In a preliminary step toward the development of osteoinductive titanium, Kokubo (1996) showed that alkali followed by thermal treatment
of pure titanium resulted in a stabilised microporous
surface structure that could form a carbonate apatite layer
in vitro and in vivo, and even bond directly to native
bone (Kokubo, 1996; Kokubo et al., 1996). Tuning this
alkali thermal treatment (10 M NaOH to 5 M NaOH) later resulted in a different nano-/microrough surface and
the induction of de novo bone (Fujibayashi et al., 2004;
Fukuda et al., 2011). However, in these same studies it
was found that apatite formation alone was not suficient to induce ectopic bone formation, despite the positive impact on osseointegration. Similarly, it is known that BCP readily forms a carbonate apatite layer in body luid (Daculsi et al., 1989; Daculsi et al., 1990), which we also
conirmed for BCP1150 and BCP1300 in simulated body luid (data not shown); however, only BCP1150 – and now BCP1150Ti with equivalent microstructure – can induce
ectopic bone formation. In agreement with the conclusion
of Fujibayashi et al. (2004), we propose that these differences hinge on microarchitecture (i.e., topography)
although apatite formation is likely a prerequisite for osteoinduction to take place because of its importance for bone-bonding. Considering that collagen ibres also iniltrate a microporous, osteoinductive surface before
de novo bone formation (Kondo et al., 2006), apatite
formation and microarchitecture may synergise to provide
a biomimetic template for both phases of bone tissue.
Because BCP1150, BCP1150Ti and BCP1300 all
shared similar Ca2+ and Pi release proiles in vitro, the
differences in bone formation are dificult to explain in terms of intrinsic differences in surface reactivity or Ca2+/P
i
signalling. However, this in vitro characterisation is limited
in light of the physico-chemical complexity of body luid
in vivo, including supersaturated Ca2+/Pi levels as well as
blood serum (Garnett and Dieppe, 1990). Other theories
on osteoinduction speculate that material degradation
by osteoclast resorption or macrophage phagocytosis may independently speed the dissolution/precipitation of a bioactive carbonate apatite layer (LeGeros, 1993), establish an instructive geometric template for de novo bone formation in resorption lacunae along with increased local Ca2+ concentrations (Klar et al., 2013; Ripamonti et al., 2008; Wilkinson et al., 2011), or liberate crystalline
nano-/microparticulate and a subsequent osteogenic cytokine cascade (Gauthier et al., 1999; Malard et al., 1999; Velard et al., 2013). However, in the present study neither characteristic osteoclast resorption lacunae nor degraded
BCP particulate were apparent in the histology.
Alternatively, decades of research have shown that surface topography can directly stimulate bone cell differentiation and function on various material substrates, including polymers (Fu et al., 2010; Watari et al., 2012;
Wilkinson et al., 2011; You et al., 2010), titanium
(Brunette, 1988; Gittens et al., 2011; McNamara et al.,
2011), ceramics (Webster, 2000; Zhang et al., 2014), and
tissue (Gray et al., 1996). Topographical control of cell
fate is a complex phenomenon that can occur through focal adhesion clustering and downstream focal adhesion kinase (FAK) signalling (McNamara et al., 2010). This cascade is
initiated when cell surface integrins bind matrix proteins
adsorbed to the substrate (Chou et al., 1995; Stevens and
George, 2005), so protein adsorption from the body luid may play a crucial role in the differences in cell-surface interactions observed in the present study. Indeed, our previous experiments showed that microstructured
BCP1150 adsorbs more proteins than denser BCP1300 (Yuan et al., 2010).
With respect to the role of osteoclasts in osteoinduction, the present study further substantiates a link between microstructure, osteoclastogenesis, and eventual de novo
bone formation. We previously reported similar indings using TCP with two different surface structures, analogous to BCP1150 and BCP1300 investigated in the present study (Davison et al., 2014b; Zhang et al., 2014). TCP possessing
surface microstructural dimensions ≤ 1 μm (TCPs) was
extensively colonised by multinucleated osteoclast-like
cells adjacent to substantial amounts of ectopic bone in
the muscle tissue of dogs after 12 weeks. In contrast, TCP
with larger surface structural dimensions (~ 2-4 μm, TCPb) contained few multinucleated cells and formed no ectopic
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
differentiation and fusion versus TCPb using the same in vitro osteoclastogenesis model applied in the present study
(Davison et al., 2014b). Taking these previous and current results together, it can be concluded that for both BCP
and TCP – representing the most frequently investigated osteoinductive materials in the literature (Barradas et al., 2011) – surface microstructural dimensions of ~ 1 μm
robustly promoted the formation of osteoclast-like cells
concurrent with de novo bone formation. These results add to the growing consensus that osteoclast formation
is prerequisite for osteoinduction (Davison et al., 2014a;
Klar et al., 2013; Kondo et al., 2006; Le Nihouannen et al., 2005); however, it is still unknown what the exact role of osteoclasts is in this process.
It has also been suggested that CaPs may stimulate bone formation by absorbing BMPs (bone morphogenetic proteins) endogenously synthesised near the implant surface (Klar et al., 2014; Ripamonti et al., 1993) or
circulating in the blood (de Groot, 1998). However,
large doses of BMPs are required to stimulate substantial amounts of de novo bone formation, likely rendering
basal levels of BMPs circulating in the blood ineffective in achieving this response (van Baardewijk et al., 2013; Yuan et al., 2010). Alternatively, BMPs or other osteogenic
factors may originate from (pre-)osteoclast interactions with microstructured surfaces including CaP (Davison et al., 2014b) and titanium (Takebe et al., 2003). Elevated Ca2+ levels resulting from osteoclast resorption of a
mineralised substrate can also stimulate BMP expression
of precursor cells (Barradas et al., 2012; Klar et al., 2013).
In support of this, osteoclast depletion by bisphosphonate treatment attenuated BMP2 expression in osteoinductive CaP implants and limited ectopic bone formation (Klar
et al., 2013), potentially because osteoclasts synthesise
a variety of BMPs (Garimella et al., 2008). Moreover,
treatment with noggin, which blocks BMP binding to
its membrane-bound receptor, also stunted ectopic bone
formation by an osteoinductive CaP (Klar et al., 2014).
However, chondrogenesis was not reported in either of these studies (Klar et al., 2013; Klar et al., 2014), or in
a thorough review of osteoinductive materials research
(Barradas et al., 2011), suggesting that osteoinduction may not proceed via a classical BMP-induced endochondral
pathway. In the broader context of bone metabolism, activated (pre-)osteoclasts secrete a variety of other
non-BMP osteogenic factors – e.g., Wnts, S1P, OSM, and
CTHRC1 – resulting in osteoblast differentiation of local precursors (Garimella et al., 2008; Guihard et al., 2012; Pederson et al., 2008; Takeshita et al., 2013) through
intramembranous ossiication (Durmus et al., 2006). To elucidate the mechanism of osteoinduction, more research
is needed to discern the distinct molecular pathways governing endochondral versus intramembranous
ossiication over the entire time course of ectopic bone
formation.
To challenge the theory that osteoclast formation promoted by surface (sub)microstructure is instrumental
for osteoinduction, osteoclastogenesis on other
osteoinductive materials should be investigated. If, for example, microstructured HA and titanium also promoted
osteoclastogenesis and ectopic bone in contrast to their
non-microstructured controls, a broader link between
osteoclast formation and de novo bone formation would be further substantiated. Pending deeper biological
insight, it may be possible to anticipate osteoinductive performance based on simpliied in vitro osteoclastogenesis
models. And, if osteoclasts are not only requisite but also directive in de novo bone formation through the secretion
of trophic factors, locally stimulating osteoclastogenesis
(i.e., controlled release of RANKL) may even render
non-microstructured CaPs osteoinductive.
Conclusion
BCP1150 and titanium-coated BCP1150Ti possessing
small surface microstructure (~ 1 μm) formed ectopic bone adjacent to multinucleated osteoclast-cells in the muscle of dogs. Implants were in the form of planar discs so
macro-scale features such as concavities, macropores and interparticle space were unnecessary for this response. In contrast, BCP1300 with identical compositional chemistry
but larger surface architecture (~ 2-4 μm) formed neither
osteoclast-like cells nor ectopic bone; it was instead encapsulated by ibrous tissue. Similar to the in vivo results, (pre-)osteoclast proliferation and differentiation
were signiicantly promoted by BCP1150 and BCP1150Ti
versus BCP1300 in vitro; moreover, osteoclasts were larger and more fused on BCP1150 versus either BCP1150Ti
or BCP1300. Together, these in vitro and in vivo results indicate that (sub)micron-scale surface architecture is the crucial material parameter versus macrostructure or
surface chemistry in stimulating both osteoclastogenesis
and ectopic bone formation in a related process.
Acknowledgements
The authors gratefully acknowledge the support of the TeRM Smart Mix Program of the Netherlands Ministry of Economic Affairs and the Netherlands Ministry of Education, Culture and Science. This research forms part
of the Project P2.04 BONE-IP of the research program
of the Biomedical Materials Institute, co-funded by the Dutch Ministry of Economic Affairs. This work was also supported by funding under the Seventh Research Framework Program of the European Union, through the project REBORNE under Grant agreement no. 241879. Special thanks are due to Dr. Zeinab Tahmasebi Birgani (MIRA) for her technical expertise with EDS. We wish to conirm that there are no known conlicts of interest
associated with this publication and there has been no
signiicant inancial support for this work that could have inluenced its outcome.
References
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
thymidine incorporation assay. J Immunol Methods 170: 211-224.
Akiyama N, Takemoto M, Fujibayashi S, Neo M, Hirano M, Nakamura T (2011) Difference between dogs and rats with regard to osteoclast-like cells in calcium-deicient hydroxyapatite-induced osteoinduction. J Biomed Mater Res A 96: 402-412.
Barradas AMC, Yuan H, van Blitterswijk CA, Habibovic P (2011) Osteoinductive biomaterials: current knowledge of properties, experimental models and
biological mechanisms. Eur Cell Mater 21: 407-429.
Barradas AMC, Fernandes HAM, Groen N, Chai YC, Schrooten J, van de Peppel J, van Leeuwen JPTM, van Blitterswijk CA, de Boer J (2012) A calcium-induced
signaling cascade leading to osteogenic differentiation of
human bone marrow-derived mesenchymal stromal cells.
Biomaterials 33: 3205-3215.
Barradas AMC, Monticone V, Hulsman M, Danoux C, Fernandes H, Tahmasebi Birgani Z, Barrère-de Groot F, Yuan H, Reinders M, Habibovic P, van Blitterswijk C, de Boer J (2013) Molecular mechanisms of biomaterial-driven osteogenic differentiation in human mesenchymal stromal
cells. Integr Biol 5: 920-931.
Baslé MF, Chappard D, Grizon F, Filmon R, Delecrin J, Daculsi G, Rebel A (1993) Osteoclastic resorption of Ca-P biomaterials implanted in rabbit bone. Calcif Tissue
Int 53: 348-356.
Beck GR, Zerler B, Moran E (2000) Phosphate is a speciic signal for induction of osteopontin gene expression. Proc Natl Acad Sci USA 97: 8352-8357.
Benahmed M, Bouler JM, Heymann D, Gan O, Daculsi G (1996) Biodegradation of synthetic biphasic calcium phosphate by human monocytes in vitro: a morphological
study. Biomaterials 17: 2173-2178.
Bongio M, van den Beucken JJJ, Nejadnik MR, Tahmasebi Birgani Z, Habibovic P, Kinard LA, Kasper FK, Mikos AG, Leeuwenburgh SCG, Jansen JA (2013)
Subcutaneous tissue response and osteogenic performance
of calcium phosphate nanoparticle-enriched hydrogels in the tibial medullary cavity of guinea pigs. Acta Biomater
9: 5464-5474.
Brunette DM (1988) The effects of implant surface topography on the behavior of cells. Int J Oral Maxillofac
Implants 3: 231-246.
Chou L, Firth JD, Uitto VJ, Brunette DM (1995) Substratum surface topography alters cell shape and regulates fibronectin mRNA level, mRNA stability, secretion and assembly in human ibroblasts. J Cell Sci
108: 1563-1573.
Collin-Osdoby P, Yu X, Zheng H, Osdoby P (2003) RANKL-mediated osteoclast formation from murine RAW
264.7 cells. Methods Mol Med 80: 153-166.
Curran JM, Chen R, Hunt JA (2006) The guidance of human mesenchymal stem cell differentiation in vitro by
controlled modiications to the cell substrate. Biomaterials
27: 4783-4793.
Daculsi G, LeGeros RZ, Nery E, Lynch K, Kerebel B (1989) Transformation of biphasic calcium phosphate
ceramics in vivo: ultrastructural and physicochemical characterization. J Biomed Mater Res 23: 883-894.
Daculsi G, LeGeros RZ, Heughebaert M, Barbieux I (1990) Formation of carbonate-apatite crystals after implantation of calcium phosphate ceramics. Calcif Tissue
Int 46: 20-27.
Davison NL, Gamblin A-L, Layrolle P, Yuan H, de Bruijn JD, Barrère-de Groot F (2014a) Liposomal clodronate
inhibition of osteoclastogenesis and osteoinduction
by submicrostructured beta-tricalcium phosphate.
Biomaterials 35: 5088-5097.
Davison NL, Luo X, Schoenmaker T, Everts V, Yuan H, Barrère-de Groot F, de Bruijn JD (2014b)
Submicron-scale surface architecture of tricalcium phosphate directs osteogenesis in vitro and in vivo. Eur Cell Mater 27: 281-297.
de Groot K (1998) Carriers that concentrate native bone
morphogenetic protein in vivo. Tissue Eng 4: 337-341.
Durmus T, LeClair RJ, Park KS, Terzic A, Yoon JK, Lindner V (2006) Expression analysis of the novel gene collagen triple helix repeat containing-1 (Cthrc1). Gene Expr Patterns 6: 935-940.
Fellah BH, Josselin N, Chappard D, Weiss P, Layrolle P (2007) Inlammatory reaction in rats muscle
after implantation of biphasic calcium phosphate micro particles. J Mater Sci Mater Med 18: 287-294.
Fu J, Wang Y, Yang MT, Desai RA, Yu X, Liu Z,
Chen CS (2010) Mechanical regulation of cell function
with geometrically modulated elastomeric substrates. Nat
Methods 7: 733-736.
Fujibayashi S, Neo M, Kim H-M, Kokubo T, Nakamura T (2004) Osteoinduction of porous bioactive titanium
metal. Biomaterials 25: 443-450.
Fukuda A, Takemoto M, Saito T, Fujibayashi S, Neo M, Pattanayak DK, Matsushita T, Sasaki K, Nishida N, Kokubo T, Nakamura T (2011) Osteoinduction of porous Ti implants with a channel structure fabricated by selective laser melting. Acta Biomater 7: 2327-2336.
Garimella R, Tague SE, Zhang J, Belibi F, Nahar N, Sun BH, Insogna K, Wang J, Anderson HC (2008) Expression and synthesis of bone morphogenetic proteins by osteoclasts : a possible path to anabolic bone remodeling J Histochem Cytochem 56: 569-577.
Garnett J, Dieppe P (1990) The effects of serum and human albumin on calcium hydroxyapatite crystal growth.
Biochem J 266: 863-868.
Gauthier O, Bouler JM, Weiss P, Bosco J, Daculsi G, Aguado E (1999) Kinetic study of bone ingrowth and
ceramic resorption associated with the implantation of different injectable calcium-phosphate bone substitutes. J Biomed Mater Res 47: 28-35.
Gauthier O, Müller R, von Stechow D, Lamy B, Weiss P, Bouler J-M, Aguado E, Daculsi G (2005) In vivo bone regeneration with injectable calcium phosphate biomaterial: a three-dimensional micro-computed
tomographic, biomechanical and SEM study. Biomaterials
26: 5444-5453.
Gittens RA, McLachlan T, Olivares-Navarrete R, Cai Y, Berner S, Tannenbaum R, Schwartz Z, Sandhage KH, Boyan BD (2011) The effects of combined micron-/
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
Gloeckner H, Jonuleit T, Lemke HD (2001) Monitoring of cell viability and cell growth in a hollow-iber bioreactor by use of the dye Alamar Blue. J Immunol Methods 252: 131-138.
Gray C, Boyde A, Jones SJ (1996) Topographically
induced bone formation in vitro: implications for bone implants and bone grafts. Bone 18: 115-123.
Guihard P, Danger Y, Brounais B, David E, Brion R, Delecrin J, Richards CD, Chevalier S, Rédini F, Heymann D, Gascan H, Blanchard F (2012) Induction of osteogenesis in mesenchymal stem cells by activated monocytes/
macrophages depends on oncostatin m signaling. Stem Cells 30: 762-772.
Habibovic P, Li J, van der Valk CM, Meijer G, Layrolle P, van Blitterswijk CA, de Groot K (2005a) Biological
performance of uncoated and octacalcium
phosphate-coated Ti6Al4V. Biomaterials 26: 23-36.
Habibovic P, Yuan H, van der Valk CM, Meijer G, van Blitterswijk CA, de Groot K (2005b) 3D microenvironment as essential element for osteoinduction by biomaterials.
Biomaterials 26: 3565-3575.
Habibovic P, Sees TM, van den Doel MA, van Blitterswijk CA, de Groot K (2006a) Osteoinduction by biomaterials--physicochemical and structural inluences. J Biomed Mater Res A 77: 747-762.
Habibovic P, Yuan H, van den Doel M, Sees TM, van Blitterswijk CA, de Groot K (2006b) Relevance of osteoinductive biomaterials in critical-sized orthotopic
defect. J Orthop Res 24: 867-876.
Halleen JM, Alatalo SL, Janckila AJ, Woitge HW, Seibel MJ, Väänänen HK (2001) Serum tartrate-resistant acid phosphatase 5b is a speciic and sensitive marker of
bone resorption. Clin Chem 47: 597-600.
Klar RM, Duarte R, Dix-Peek T, Dickens C, Ferretti C, Ripamonti U (2013) Calcium ions and osteoclastogenesis initiate the induction of bone formation by coral-derived
macroporous constructs. J Cell Mol Med 17: 1444-1457.
Klar RM, Duarte R, Dix-Peek T, Ripamonti U (2014) The induction of bone formation by the recombinant human transforming growth factor-β3. Biomaterials 35: 2773-2788.
Kokubo T (1996) Formation of biologically active bone-like apatite on metals and polymers by a biomimetic process. Thermochim Acta 280-281: 479-490.
Kokubo T, Miyaji F, Kim H-M, Nakamura T (1996) Spontaneous formation of bonelike apatite layer on chemically treated titanium metals. J Am Ceram Soc 79: 1127-1129.
Kondo N, Ogose A, Tokunaga K, Umezu H, Arai K, Kudo N, Hoshino M, Inoue H, Irie H, Kuroda K, Mera H, Endo N (2006) Osteoinduction with highly puriied
beta-tricalcium phosphate in dog dorsal muscles and the proliferation of osteoclasts before heterotopic bone formation. Biomaterials 27: 4419-4427.
LeGeros RZ (1993) Biodegradation and bioresorption
of calcium phosphate ceramics. Clin Mater 14: 65-88.
LeGeros RZ (2008) Calcium phosphate-based osteoinductive materials. Chem Rev 108: 4742-4753.
Le Nihouannen D, Daculsi G, Saffarzadeh A, Gauthier O, Delplace S, Pilet P, Layrolle P (2005) Ectopic bone formation by microporous calcium phosphate ceramic
particles in sheep muscles. Bone 36: 1086-1093.
Ljusberg J, Ek-Rylander B, Andersson G (1999) Tartrate-resistant purple acid phosphatase is synthesized as a latent proenzyme and activated by cysteine proteinases.
Biochem J 343: 63-69.
Magan A, Ripamonti U (1996) Geometry of porous hydroxyapatite implants influences osteogenesis in
baboons (Papio ursinus). J Craniofac Surg 7: 71-78.
Makihira S, Mine Y, Kosaka E, Nikawa H (2007) Titanium surface roughness accelerates
RANKL-dependent differentiation in the osteoclast precursor cell
line, RAW264. 7. Dent Mater J 26: 739-745.
Malard O, Bouler JM, Guicheux J, Heymann D, Pilet P, Coquard C, Daculsi G (1999) Inluence of biphasic calcium phosphate granulometry on bone ingrowth, ceramic resorption, and inlammatory reactions: preliminary in vitro and in vivo study. J Biomed Mater Res 46: 103-111.
McNamara LE, McMurray RJ, Biggs MJP, Kantawong F, Oreffo ROC, Dalby MJ (2010) Nanotopographical control of stem cell differentiation. J Tissue Eng 2010: 120623.
McNamara LE, Sjöström T, Burgess KE V, Kim JJW, Liu E, Gordonov S, Moghe P V, Meek RMD, Oreffo ROC, Su B, Dalby MJ (2011) Skeletal stem cell physiology on functionally distinct titania nanotopographies. Biomaterials
32: 7403-7410.
Nakayama GR, Caton MC, Nova MP, Parandoosh Z (1997) Assessment of the Alamar Blue assay for cellular growth and viability in vitro. J Immunol Methods 204: 205-208.
Pederson L, Ruan M, Westendorf JJ, Khosla S, Oursler MJ (2008) Regulation of bone formation by osteoclasts involves Wnt/BMP signaling and the chemokine sphingosine-1-phosphate. Proc Natl Acad Sci USA 105: 20764-20769.
Ripamonti U (1991) The morphogenesis of bone in replicas of porous hydroxyapatite obtained from conversion of calcium carbonate exoskeletons of coral. J Bone Joint Surg Am 73: 692-703.
Ripamonti U, van den Heever B, van Wyk J (1993) Expression of the osteogenic phenotype in porous hydroxyapatite implanted extraskeletally in baboons. Matrix 13: 491-502.
Ripamonti U, Richter PW, Nilen RWN, Renton L (2008) The induction of bone formation by smart biphasic hydroxyapatite tricalcium phosphate biomimetic matrices
in the non-human primate Papio ursinus. J Cell Mol Med 12: 2609-2621.
Ripamonti U, Klar RM, Renton LF, Ferretti C (2010) Synergistic induction of bone formation by hOP-1, hTGF-beta3 and inhibition by zoledronate in macroporous coral-derived hydroxyapatites. Biomaterials 31: 6400-6410.
Stevens MM, George JH (2005) Exploring and
NL Davison et al. Osteoinduction and osteoclastogenesis by BCP discs
Syed-Picard FN, Jayaraman T, Lam RSK, Beniash E, Sfeir C (2013) Osteoinductivity of calcium phosphate mediated by connexin 43. Biomaterials 34: 3763-3774.
Takahashi N, Udagawa N, Kobayashi Y, Suda T (2007) Generation of osteoclasts in vitro, and assay of osteoclast
activity. Methods Mol Med 135: 285-301.
Takebe J, Champagne CM, Offenbacher S, Ishibashi K, Cooper LF (2003) Titanium surface topography alters
cell shape and modulates bone morphogenetic protein 2
expression in the J774A.1 macrophage cell line. J Biomed Mater Res A 64: 207-216.
Takeshita S, Fumoto T, Matsuoka K, Park K, Aburatani H, Kato S, Ito M, Ikeda K (2013) Osteoclast-secreted CTHRC1 in the coupling of bone resorption to formation. J Clin Invest 123: 3914-3924.
van Baardewijk LJ, van der Ende J, Lissenberg-Thunnissen S, Romijn LM, Hawinkels LJAC, Sier CFM,
Schipper IB (2013) Circulating bone morphogenetic
protein levels and delayed fracture healing. Int Orthop 37: 523-527.
Velard F, Braux J, Amedee J, Laquerriere P (2013) Inflammatory cell response to calcium phosphate biomaterial particles: an overview. Acta Biomater 9: 4956-4963.
Vlacic-Zischke J, Hamlet SM, Friis T, Tonetti MS, Ivanovski S (2011) The influence of surface microroughness and hydrophilicity of titanium on the up-regulation of TGFβ/BMP signalling in osteoblasts.
Biomaterials 32: 665-671.
Watari S, Hayashi K, Wood JA, Russell P, Nealey PF, Murphy CJ, Genetos DC (2012) Modulation of osteogenic differentiation in hMSCs cells by submicron topographically-patterned ridges and grooves. Biomaterials
33: 128-136.
Webster T (2000) Enhanced functions of osteoblasts
on nanophase ceramics. Biomaterials 21: 1803-1810.
Webster TJ, Ergun C, Doremus RH, Siegel RW, Bizios R (2001) Enhanced osteoclast-like cell functions on
nanophase ceramics. Biomaterials 22: 1327-1333.
Wilkinson A, Hewitt RN, McNamara LE, McCloy D, Dominic Meek RM, Dalby MJ (2011) Biomimetic microtopography to enhance osteogenesis in vitro. Acta Biomater 7: 2919-2925.
Wolke JG, de Groot K, Jansen JA (1998) In vivo
dissolution behavior of various RF magnetron sputtered
Ca-P coatings. J Biomed Mater Res 39: 524-530.
Yamada S, Heymann D, Bouler JM, Daculsi G (1997)
Osteoclastic resorption of calcium phosphate ceramics with
different hydroxyapatite/beta-tricalcium phosphate ratios.
Biomaterials 18: 1037-1041.
Yamasaki H, Sakai H (1992) Osteogenic response to porous hydroxyapatite ceramics under the skin of dogs.
Biomaterials 13: 308-312.
You M-H, Kwak MK, Kim D-H, Kim K, Levchenko A, Kim D-Y, Suh K-Y (2010) Synergistically enhanced osteogenic differentiation of human mesenchymal stem cells by culture on nanostructured surfaces with induction
media. Biomacromolecules 11: 1856-1862.
Yuan H, de Bruijn JD (2011) Osteoinductive calcium phosphates. United States Patent 7,942,934 B2: 1-27. Yuan H, Yang Z, Li Y, Zhang X, de Bruijn JD, de Groot K (1998) Osteoinduction by calcium phosphate
biomaterials. J Mater Sci Mater Med 9: 723-726.
Yuan H, Kurashina K, de Bruijn JD, Li Y, de Groot K, Zhang X (1999) A preliminary study on osteoinduction of two kinds of calcium phosphate ceramics. Biomaterials
20: 1799-1806.
Yuan H, van den Doel M, Li S, Van Blitterswijk CA, de Groot K, de Bruijn JD (2002) A comparison of the osteoinductive potential of two calcium phosphate ceramics implanted intramuscularly in goats. J Mater Sci
Mater Med 13: 1271-1275.
Yuan H, Fernandes H, Habibovic P, de Boer J, Barradas AMC, de Ruiter A, Walsh WR, van Blitterswijk CA, de Bruijn JD (2010) Osteoinductive ceramics as a synthetic alternative to autologous bone grafting. Proc Natl Acad Sci USA 107: 13614-13619.
Zhang J, Luo X, Barbieri D, Barradas AMC, de Bruijn JD, van Blitterswijk CA, Yuan H (2014) The size of
surface microstructures as an osteogenic factor in calcium
phosphate ceramics. Acta Biomater 10: 3254-3263.
Zhao G, Raines AL, Wieland M, Schwartz Z, Boyan BD (2007) Requirement for both micron- and submicron scale structure for synergistic responses of osteoblasts to substrate surface energy and topography. Biomaterials 28: 2821-2829.
Editor’s Note: All questions/comments by the reviewers